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Adipose tissue is an ideal source of mesenchymal stem cells for bone tissue engineering: it is largely dispensable and readily accessible with minimal morbidity. However, the stromal vascular fraction (SVF) of adipose tissue is a heterogeneous cell population, which leads to unreliable bone formation. In the present study, we prospectively purified human perivascular stem cells (PSCs) from adipose tissue and compared their bone-forming capacity with that of traditionally derived SVF. PSCs are a population (sorted by fluorescence-activated cell sorting) of pericytes (CD146+CD34−CD45−) and adventitial cells (CD146−CD34+CD45−), each of which we have previously reported to have properties of mesenchymal stem cells. Here, we found that PSCs underwent osteogenic differentiation in vitro and formed bone after intramuscular implantation without the need for predifferentiation. We next sought to optimize PSCs for in vivo bone formation, adopting a demineralized bone matrix for osteoinduction and tricalcium phosphate particle formulation for protein release. Patient-matched, purified PSCs formed significantly more bone in comparison with traditionally derived SVF by all parameters. Recombinant bone morphogenetic protein 2 increased in vivo bone formation but with a massive adipogenic response. In contrast, recombinant Nel-like molecule 1 (NELL-1; a novel osteoinductive growth factor) selectively enhanced bone formation. These studies suggest that adipose-derived human PSCs are a new cell source for future efforts in skeletal regenerative medicine. Moreover, PSCs are a stem cell-based therapeutic that is readily approvable by the U.S. Food and Drug Administration, with potentially increased safety, purity, identity, potency, and efficacy. Finally, NELL-1 is a candidate growth factor able to induce human PSC osteogenesis.
Since the original description of adipose tissue as a source of adult multilineage stem cells , the preclinical study of adipose-derived cells for repair and regeneration of tissues has increased dramatically (reviewed in ). The theoretical advantages of adipose-derived cells over other cell types for biologic bone regeneration strategies are numerous. For example, although autograft bone remains the gold standard for bone repair, its disadvantages are significant, including donor site morbidity, extended operating time complications, and limited autogenous supply [3–5]. On the other hand, bone marrow mesenchymal stem cells (BMSCs) have long been studied for their application to skeletal engineering. However, BMSCs have distinct disadvantages over adipose-derived cells, including limitations in autogenous supply of bone marrow aspirate as compared with lipoaspirate, and relatively lower cell yield of BMSCs in comparison with adipose-derived stem cells (ASCs) (estimated at ~104 stem cells vs. ~106 stem cells per 40 ml) [6–8]. Finally, human ASCs have been used successfully to heal small animal [9, 10] and large animal  skeletal defects.
Despite the advantages of fat tissue-derived cells for bone regeneration, there exist clear hurdles that must be overcome for their successful clinical use. For example, adipose-derived stromal cells are defined by their adherence to cell culture plates and ex vivo expansion. This ex vivo expansion increases the risk of immunogenicity, infection, and genetic instability [12, 13]. As an alternative to ASCs, the cells of noncultured total stromal vascular fraction (SVF) from adipose tissues have been used. Available studies using SVF show poor and unreliable bone formation  or lower bone regeneration efficacy relative to cultured ASCs . SVF of adipose tissue is a highly heterogeneous cell population, including nonmesenchymal stem cell types, such as inflammatory cells, hematopoietic stem cells, and endothelial cells, among others . Variability in cell composition presents clear disadvantages for U.S. Food and Drug Administration (FDA) approval of a future stem cell-based therapeutic, potentially including reduced safety, purity, identity, potency, and efficacy. Notably, these are the criteria upon which the Center for Biologics Evaluation and Research evaluates stem cell-based product applications . For example, given the heterogeneity of SVF, precise product characterization is not feasible, leading to lack of human stromal vascular fraction (hSVF) product identity. Batch-to-batch variability and nonuniformity in effect (again attributable to variable stem cell content) reduces the efficacy and potency of hSVF compounds and potentially reduces product safety. With these regulatory hurdles in mind, our approach was to reduce the inherent heterogeneity within hSVF to obtain a safer and more efficacious stem cell-based therapeutic.
To address this issue of SVF heterogeneity, previous investigators have used fluorescence-activated cell sorting (FACS) to purify fat-derived cell populations, with some success. For example, cell sorting of adipose tissue has allowed for enrichment of osteoprogenitor  or chondroprogenitor  cell types—but not the isolation of multipotent mesenchymal stem cells (MSCs). Our solution has been to identify the native perivascular phenotype of MSCs and prospectively isolate perivascular MSCs using multicolor FACS. We have previously shown two populations of perivascular stem cells (PSCs) associated with blood vessels [20–24]. These include CD34−CD146+CD45− pericytes surrounding microvessels and capillaries [20, 25] and a second distinct adventitial cell (CD34+CD146−CD45−) , associated with larger blood vessels. Both cell types are isolatable from adipose tissue and resemble MSCs by morphology, growth, surface markers, and clonal multilineage differentiation potential [20–24].
In this report, we describe the use of a novel, FACS-purified cell source for improved bone tissue engineering: human perivascular stem cells (hPSCs). Using an intramuscular, ectopic bone model, we observed that adipose-derived, FACS-isolated hPSCs formed bone to a greater degree than patient-matched, unsorted hSVF. Next, two growth factors were examined for their osteoinductive effects: bone morphogenetic protein 2 (BMP2) and Nel-like molecule-1 (NELL-1). The novel cytokine NELL-1 was identified as an appropriate osteogenic stimulus rather than BMP2, which had pleiotropic effects, including adipogenic differentiation and cyst-like bone formation.
Human lipoaspirate (n = 70 donors) was obtained from patients undergoing cosmetic liposuction. No patient identifiers were obtained. Lipoaspirate was stored for no more than 128 hours at 4°C before processing. The hSVF was obtained by collagenase digestion as previously described . Briefly, lipoaspirate was diluted with an equal volume of phosphate-buffered saline (PBS) before digestion with Dulbecco's modified Eagle's medium (DMEM) containing 3.5% bovine serum albumin (Sigma-Aldrich, St. Louis, http://www.sigmaaldrich.com) and 1 mg/ml type II collagenase for 70 minutes under agitation at 37°C. Next, adipocytes were separated and removed by centrifugation. The pellet was then resuspended in red-cell lysis buffer (155 mM NH4Cl, 10 mM KHCO3, and 0.1 mM EDTA) and incubated for 10 minutes at room temperature. After centrifugation, pellets were resuspended in PBS and filtered at 70 μm. The resulting hSVF was either further processed for cell sorting (to isolate PSCs) or used immediately for in vivo application. In order to calculate live cell number for implantation, trypan blue staining was performed to assess cell viability. Cells were kept on ice until in vivo implantation. n = 70 patient samples were used for in vitro experiments, and n = 6 patient samples were used for in vivo experiments; demographics were recorded, including age, sex, and anatomic location of harvest, and are presented in supplemental online Table 1.
PSCs were purified by FACS of the hSVF as previously described . hSVF was incubated with a mixture of the following directly conjugated antibodies: anti-CD34-phycoerythrin (1:100; Dako, Glostrup, Denmark, http://www.dako.com), anti-CD45-allophycocyanin (1:100; Santa Cruz Biotechnology Inc., Santa Cruz, CA, http://www.scbt.com), and anti-CD146-fluorescein isothiocyanate (1:100; AbD Serotec, Raleigh, NC, http://www.ab-direct.com). All incubations were performed at 4°C for 15 minutes in the dark. Before sorting, 4′,6-diamidino-2-phenylindole (DAPI; 1:1,000; Invitrogen, Carlsbad, CA, http://www.invitrogen.com) was added for dead cell exclusion; the solution was then passed through a 70-μm cell filter and then run on a FACSAria cell sorter (BD Biosciences, San Diego, CA, http://www.bdbiosciences.com). Sorted cells were used for in vivo application immediately or plated for in vitro studies. In this manner, distinct microvessel pericytes (CD34−, CD146+, CD45−) and adventitial cells (CD34+, CD146−, CD45−) were isolated and combined to constitute the PSC population. For select experiments, fluorescent labeling of live cells was performed prior to implantation using PKH26 fluorescent cell linker (Sigma-Aldrich). Cells were kept on ice until in vivo implantation.
The expansion of cells was performed in DMEM, 20% fetal bovine serum (FBS), 1% penicillin/streptomycin. Osteogenic differentiation of human PSCs was performed as previously described [9, 27], with minor modifications. Passage 4 PSCs were seeded at a density of 35,000 cells per well in 12-well plates. Differentiation medium consisted of DMEM, 10% FBS, 100 μg/ml ascorbic acid, and 10 mM β-glycerophosphate. Assessments, including alkaline phosphatase and alizarin red staining, were performed as previously described [10, 28].
Implants were prepared as per supplemental online Tables 2–5. Two different scaffolds were used for cell delivery. First, an absorbable collagen sponge of defined dimensions (0.5 × 1 × 1.5 cm) (component of the INFUSE Bone Graft; Medtronic, Minneapolis, MN, http://www.medtronic.com) was used (data presented in Fig. 1). This carrier was chosen as a nonosteoinductive carrier, as intramuscular implantation of absorbable collagen sponge alone is known to have no bone forming effects . Second, an ovine DBX Putty was used (100 μl; Musculoskeletal Transplant Foundation, Edison, NJ, http://www.mtf.org). DBX Putty combines morselized cortical-cancellous demineralized bone chips with sodium hyaluronate, and it was chosen for its proven osteoinductive characteristics and clinical translation (human demineralized bone matrix [DBX] is already 510(k) approved) (data presented in Figs. 22–5). Select experiments added growth factors (recombinant human BMP2 or NELL-1), which were lyophilized onto tricalcium phosphate (β-TCP) particles (Chronos β-TCP granules, 200–300 μm diameter; Synthes, West Chester, PA, http://www.synthes.com) and stored at 4°C prior to use. This avoids burst-type release kinetics in favor of sustained growth factor release . Concentrations of BMP2 were based on the clinical-range doses needed for human bone formation (up to 1,500 μg/ml) rather than the lower doses more commonly used in mice . Concentrations of NELL-1 were based on our previous publication using an intramuscular model and fetal pancreatic pericytes . The individual components (DBX + β-TCP) were mixed mechanically prior to implantation. Finally, defined numbers of viable cells in PBS suspension (20 μl) from the hSVF or PSCs were applied (either allowed to soak into absorbable collagen sponge or mechanically mixed with DBX/β-TCP). The cell + scaffold suspension was kept on ice until implantation.
Intramuscular implantation was performed in 8-week-old male SCID mice. Animals were anesthetized by isoflurane inhalation (5% induction, 2% maintenance) and premedicated with 0.05 mg/kg buprenorphine. Bilateral incisions in the hind limbs were made, and pockets were cut in the biceps femoris muscles by blunt dissection, parallel to the muscle fiber long axis. Implants were placed bilaterally; implant compositions are fully described in supplemental online Tables 2–6. Numbers of animals per experiment can be found in the figure legends. The fasciae overlying the muscle were sutured with a simple continuous pattern, and the skin was closed in a separate layer using 5-0 Vicryl (Ethicon, San Angelo, TX, http://www.ecatalog.ethicon.com) sutures in a subcuticular pattern. Animals were postoperatively treated with buprenorphine for 48 hours and trimethoprim/sulfamethoxazole for 10 days for pain management and infection prevention, respectively. Animals were housed and experiments were performed in accordance with guidelines of the Chancellor's Animal Research Committee of the Office for Protection of Research Subjects at the University of California, Los Angeles.
Live high-resolution radiographs were taken every 2 weeks for select experiments using a cabinet radiography system (Faxitron Bioptics, Lincolnshire, IL, http://www.faxitron.com). Mice were anesthetized using isoflurane (5% induction, 2% maintenance).
Samples were harvested en bloc from 4 to 6 weeks postimplantation, formalin-fixed, and imaged using high-resolution microcomputed tomography (microCT) (Skyscan 1172F; Skyscan, Kontich, Belgium, http://www.skyscan.be) at an image resolution of 19.73 μm and analyzed using DataViewer, Recon, CTAn, and CTVol programs provided by the manufacturer. For computed tomography (CT) data analysis, the region of interest includes the entire volume of the scanned muscle pouch excluding the native femur to quantify bone volume (BV) and bone mineral density (BMD). Threshold values for three-dimensional reconstructions and quantification can be found in the figure legends. All quantitative and structural morphometric data use nomenclature described by the American Society for Bone and Mineral Research Nomenclature Committee .
After CT analysis, samples were decalcified in 19% EDTA and embedded in paraffin. Hematoxylin and eosin (H&E) and Movat's pentachrome staining were performed as previously described . For select experiments, bone formation was quantified by blinded histomorphometric analyses using H&E staining (Figs. 2, ,6)6) and Photoshop (Adobe Systems Inc., San Jose, CA, http://www.adobe.com) quantification as expressed by mean bone area and bone area/tissue area . For select experiments, adipogenesis was quantified by blinded calculations of lipid droplet number per ×100 field (Fig. 4). Immunohistochemistry was performed with primary antibodies against bone sialoprotein (Chemicon, Temecula, CA, http://www.chemicon.com), osteocalcin (Santa Cruz Biotechnology), and major histocompatibility complex (MHC) class I surface antigen (Santa Cruz Biotechnology) using the ABC (Vector Laboratories, Burlingame, CA, http://www.vectorlabs.com) method. Select quantification of immunohistochemistry was performed again using the magic wand tool in Photoshop with a tolerance setting of 30 (Fig. 2).
Statistical analysis was performed using an appropriate analysis of variance test when more than two groups were compared, followed by Student's t test to compare two groups. Inequality of SDs was excluded by using Levene's test. p ≤ .05 was considered to be significant.
We recently described, purified, and characterized two perivascular sources of primary MSCs within human adipose tissue based on the expression of CD34 and CD146. Pericytes, which are surrounding microvessels, are isolatable from multiple human organs, including adipose tissue, and are CD146+CD34−CD45− [20, 25]. More recently, we have described a second and distinct perivascular MSC population, adventitial cells (CD146−CD34+CD45−) , obtainable from human adipose among other tissues. Here, we first confirmed our previous results, showing that pericytes (CD146+CD34−) and adventitial cells (CD146−CD34+) are distinct populations isolatable from human lipoaspirate after exclusion of CD45+ cells (hematopoietic cells) and DAPI+ cells (dead cells) (Fig. 6). Both pericytes and adventitial cells have been previously reported to undergo multiple mesodermal lineage differentiation [20, 26]. With n = 70 unique samples of lipoaspirate, we observed the mean prevalence of pericytes and adventitial cells to be 17.1% and 22.5% of the total viable cell yield of SVF. From a tissue-engineering standpoint, maximal MSC yield per unit of autologous tissue removed would improve efficacy for tissue engineering while reducing harvest morbidity. For this reason, we chose to combine both perivascular MSC populations—collectively termed PSCs—to maximize cell yield for our efforts in bone engineering (collectively, PSCs make up, on average, 39.6% of total viable SVF). Importantly, those cells within adipose tissue that are neither pericytes (CD146+CD34−) nor adventitial cells (CD146−CD34+) do not express typical MSC markers or undergo mesodermal lineage differentiation .
hPSCs were first evaluated for their ability to undergo osteogenic differentiation in vitro and bone forming potential in vivo (Fig. 1). In standard osteogenic medium, hPSCs showed robust alkaline phosphatase staining after 5 days in differentiation medium and bone nodule formation after 10 days in differentiation medium (Fig. 1A, A,1B).1B). Freshly derived hPSCs were next placed on a collagen sponge without predifferentiation or growth factor stimulation and inserted intramuscularly (see supplemental online Table 2 for treatment groups). Over the course of 6 weeks, spontaneous mineralization was observed by radiography (Fig. 1C), three-dimensional CT (Fig. 1D), and histology (Fig. 1E, E,1F).1F). In contrast, intramuscular implantation of absorbable collagen sponge alone is known to have no bone forming effects . Collectively, these studies showed that hPSCs (like their individual pericyte and adventitial components) undergo osteogenic differentiation in vitro and in vivo and thus may be useful as a purified cell source for bone formation.
Having demonstrated that hPSCs are an osteocompetent cell source, we next sought to directly compare bone formation in patient-matched, purified hPSCs to unsorted hSVF. For this head-to-head determination, the same numbers of viable hSVF cells or hPSCs were implanted (2.5 × 105) intramuscularly. An osteoinductive carrier was used: demineralized bone matrix (DBX Putty), which consists of morselized cortical-cancellous demineralized bone chips with sodium hyaluronate (Musculoskeletal Transplant Foundation) (see supplemental online Table 3 for treatment groups). At 4 weeks postimplantation, two- and three-dimensional CT images showed significantly increased bone formation in hPSC in comparison to hSVF samples (Fig. 2A, A,2B).2B). CT quantification demonstrated a statistically significant increase in BV and BMD in hPSC-treated samples (Fig. 2C, C,2D).2D). Histologic analysis was performed by routine H&E (Fig. 2E). Histomorphometric quantification of bone area per random high-powered field showed increased bone among hPSC-treated samples (Fig. 2F). Immunohistochemical staining for the bone-specific markers bone sialoprotein and osteocalcin was performed (Fig. 2G, G,2I).2I). In each instance, photographic quantitation of positive staining intensity showed a significant increase in both bone markers in hPSC-treated specimens (Fig. 2H, H,2J).2J). Importantly, we confirmed that those cells surrounding and interspersed between bone chips were of predominantly human origin (Fig. 3), using immunohistochemical staining for MHC class I human surface antigen (Fig. 3A) or via fluorescent labeling of hSVF cells or hPSCs prior to implantation (Fig. 3B). Thus, equivalent numbers of purified hPSCs result in increased ectopic bone formation in comparison with patient-matched hSVF cells.
Having demonstrated that equal numbers of hPSCs form increased bone as compared with hSVF, we next asked as to whether this difference could be overcome by simply adding more hSVF cells. For this purpose, two concentrations of cells were used in the same intramuscular model: either 2.5 × 104 or 2.5 × 105 cells per implant. All hSVF or hPSC samples were patient-matched. If reduced MSC numbers were the only difference between hSVF and hPSC, then increasing the hSVF cell number 10-fold would surely mitigate any observed differences. However, we found this not to be the case (supplemental online Fig. 1). Namely, hPSCs formed greater bone irrespective of cell concentration than hSVF. This was observed by microCT reconstructions of representative samples (supplemental online Fig. 1A), microCT quantifications of BV and BMD (supplemental online Fig. 1B, 1C), and representative histological fields (supplemental online Fig. 1D, 1E). Thus, a simple reduction in stem cell number likely does not explain the difference in bone formation between hSVF and purified hPSC.
The most commonly used growth factor for bone regeneration is BMP2 (INFUSE Bone Graft) . We next sought to determine whether BMP2 would be an appropriate stimulus for hPSC bone formation (see supplemental online Table 4 for treatment groups). Two-dimensional axial CT scans showed a clear increase in bone formation among both hSVF- and hPSC-treated samples in response to BMP2 (Fig. 4A, A,4B).4B). In addition, a striking trend was observed in which a thin cortical shell (indicated by white arrows in Fig. 4A) was observed in BMP2-treated specimens that extended well beyond the usual ectopic bone margins (Fig. 4A, A,4B).4B). Quantification of BV and BMD were next performed with BMP2-treated specimens. First, we again found that BV and BMD were increased in hPSC as compared with hSVF-treated samples (Fig. 4C, C,4D,4D, far left). However, the effects of BMP2 were to some extent unexpected. Although BMP2 produced a significant increase in BV (Fig. 4C), it had a negative and opposing effect on BMD as compared with hSVF or hPSC alone (Fig. 4D). Histological evaluation was more revealing (Fig. 4E, E,4F).4F). In hSVF and hPSC samples without BMP2, bone chips were closer together (Fig. 4E) and were interspersed with cells with fibroblastic morphology (Fig. 4F, left). In BMP2-treated hSVF or hPSC samples, however, bone chips were farther apart and predominantly interspersed with lipid droplets (Fig. 4F). In order to quantify the adipogenic response produced by BMP2, relative lipid droplet number per ×100 field was determined. Within both hSVF- and hPSC-treated samples, BMP2 induced a statistically significant increase in lipid droplet number (Fig. 4G). Thus, BMP2 had both pro-osteogenic and also proadipogenic effects within both hSVF- and hPSC-treated implants and may not be the most appropriate cytokine stimulus for induction of hPSC-mediated high-quality bone formation.
In clinical practice, the only approved growth factor alternative to BMP2 is BMP7 (or OP-1; Stryker, Kalamazoo, MI, http://www.stryker.com); however, BMP7 is also known to have proadipogenic effects [36, 37]. In contrast, NELL-1 is a growth factor in preclinical development that has potent pro-osteogenic effects in small and large mammalian models (reviewed in ) and has been recently described to have antiadipogenic effects . NELL-1 was next added to hSVF- or hPSC-laden intramuscular implants (see supplemental online Table 5 for treatment groups). At 4 weeks postimplantation, hPSC-treated implants again showed increased bone formation in comparison with hSVF, as shown by CT reconstructions (Fig. 5A, A,5B)5B) and quantification (Fig. 5C, C,5D).5D). The addition of NELL-1 led to a significant increase in BV and BMD among hPSC-treated implants (Fig. 5C, C,5D,5D, far right column). Histologic and histomorphometric analysis revealed similar findings between treatment groups (Fig. 5E–5H). Bone chips were noted to be closer together among hPSC-treated or hPSC + NELL-1-treated implants (Fig. 5E, E,5F).5F). Histomorphometric calculations of bone area and bone area/tissue area confirmed these observations (Fig. 5G, G,5H).5H). A significant increase in both parameters was observed between hPSC-treated and hSVF-treated implants. Moreover, hPSC + NELL-1 led to a significant increase over hPSC treatment alone. Unlike BMP2, minimal lipid was observed among NELL-1-treated samples.
For the first time, we have shown that a purified population of adipose-derived stem cells (hPSCs) is superior to hSVF for bone tissue regeneration. We have shown this in terms of potency (increased bone formation over unsorted hSVF), identity, and purity (defined cell surface markers yielding an MSC population of increased homogeneity without extraneous materials and other cell lineages, such as hematopoietic and endothelial). In theory, hPSCs would also demonstrate improved potency over hSVF, as a defined and homogeneous cell population would have more predictable in vivo outcomes than a nonhomogeneous mixture. Moreover, hPSCs are an attractive cell source, as they are plentiful within adipose tissue (on average constituting ~40% of total viable hSVF). In this regard, even those patients with minimal excess body fat could donate autologous fat tissue for hPSC harvest. Moreover, sufficient quantities of hPSCs could be harvested without the need for time-consuming and costly in vitro expansion. Avoidance of in vitro expansion also reduces the risk of immunogenicity, infection, and genetic instability [12, 13].
Although hPSCs showed improved bone formation in comparison with hSVF cells across all experiments and all parameters, the underlying mechanism by which hPSCs produce higher bone formation is only partially elucidated. One explanation is that hSVF simply contains fewer MSCs than a purified hPSC population. However, our experiments refute this hypothesis. For example, adding hSVF cells at a 10:1 ratio in comparison with hPSCs still led to inferior bone formation (supplemental online Fig. 1). Another possible explanation is that within hSVF there exists a differentiation-inhibiting cell type. In this regard, endothelial cells have been described to negatively regulate the differentiation of MSCs, such as ASCs or BMSCs [39, 40]. For instance, human endothelial cells inhibit BMSC differentiation into mature osteoblasts by interfering with Osterix expression . With this evidence in mind, hPSCs (which are CD31−) may show enhanced bone formation in part by elimination of the endothelial cell component. Finally, the trophic effect of hPSCs should not be overlooked. Perivascular cells have been observed to secrete high levels of pro-osteogenic, provasculogenic growth factors, such as vascular endothelial growth factor, fibroblast growth factor 2, and epidermal growth factor . PSCs may induce robust in vivo bone formation largely through trophic effects via paracrine induction of vasculogenesis and osteogenesis.
The marriage of an osteocompetent cell source with osteoinductive growth factors is a logical union for skeletal tissue engineering. We examined both BMP2 and NELL-1 as candidate growth factors. BMP2 (INFUSE Bone Graft) is the main FDA-approved osteoinductive factor, but it has significant undesirable side effects, including life-threatening cervical swelling , osteoclast activation , adipogenic differentiation , and bone cyst formation [44, 45]. In particular to our study, we found that BMP2 induced a massive adipogenic response and showed poor bone quality (reduced bone mineral density) (Fig. 4). This is in line with BMP2's known effects in enhancing the transcription and activity of peroxisome proliferator-activated receptor γ, the main transcription factor regulating adipocyte lineage commitment [46, 47]. In contrast, NELL-1 showed a more osteospecific response, with no apparent induction of adipogenesis (Fig. 5). Our laboratory's previous publications show that exogenous NELL-1 induces significant bone formation in such models as critical sized rat calvarial defects ; rat femoral segmental defects ; and spinal fusion in rat [30, 49], sheep , and nonhuman primate models (manuscript in preparation). The pro-osteogenic effect of NELL-1 was also recently reported using pericytes derived from fetal pancreas in an intramuscular ectopic bone environment .
In summary, these data show that hPSCs are readily obtainable from human lipoaspirate. Moreover, hPSCs are able to form bone in vivo without the need for predifferentiation. Next, uncultured hPSCs were observed to be superior to patient-matched hSVF with respect to the quantity and quality of bone formation. Finally, through a series of in vivo experiments, we have optimized a combination product for local bone formation by delivering autologous, purified adult hPSCs and an osteoinductive protein (NELL-1) on an acellular allograft bone scaffold.
PSCs not only show improved efficacy in bone formation relative to sample-matched hSVF but also show improvements in other parameters for FDA approval. These include enhanced purity and identity (PSCs are an MSC population containing no hematopoietic stem cells, endothelial cells, or nonviable cells), and potency (as a more defined cell population, hPSCs will likely have reduced variability in effect as compared with hSVF). In fact, the intramuscular implantation assay described may well serve as an easily replicable assay for hPSC potency in bone formation. Excitingly, recent studies have already demonstrated the utility of perivascular stem cells for regeneration of disparate tissue types, including skeletal muscle , lung , and even myocardium . Further studies will extend our findings and apply the robust osteogenic potential of hPSCs to the healing of bone defects.
This work was supported by California Institute for Regenerative Medicine (CIRM) Early Translational II Research Award TR2-01821, the NIH/National Institute of Dental and Craniofacial Research (Grants R21-DE0177711 and R01-DE01607), University of California Discovery Grant 07-10677, T32 training fellowship (5T32DE007296-14; to A.W.J.), and a CIRM Training Grant Research Fellowship (TG-01169; to M.C. and J.N.Z.).
A.W.J. and J.N.Z.: conception and design, collection and/or assembly of data, data analysis and interpretation, manuscript writing; X.Z., R.G., and J.S.: collection and/or assembly of data, data analysis and interpretation, manuscript writing; A.A., M. Chiang, W.Y., L.C., M. Corselli, and S.P.: collection and/or assembly of data, data analysis and interpretation; D.S. and B.W.: provision of study material; K.T.: financial support, administrative support, manuscript writing; B.P. and C.S.: conception and design, financial support, administrative support, manuscript writing, final approval of manuscript.
X.Z., K.T., B.W., and C.S. are inventors of NELL-1 related patents, and K.T., B.P., and C.S. are inventors of perivascular stem cell-related patents filed from the University of California, Los Angeles. X.Z., K.T., B.W., and C.S. are founders of Bone Biologics Inc., which sublicenses NELL-1 patents from the University of California Regents, and K.T. and C.S. are founders of Scarless Laboratories Inc., which sublicenses perivascular stem cell-related patents from the University of California Regents. C.S. is also an officer of Scarless Laboratories, Inc.